Detecting high-grade squamous intraepithelial
lesions in the cervix with quantitative
spectroscopy and per-patient normalization
Jelena Mirkovic,1,2* Condon Lau,1 Sasha McGee,1 Christopher Crum,2
Kamran Badizadegan,3 Michael Feld,1 and Elizabeth Stier4
1
George R. Harrison Spectroscopy Laboratory, Massachusetts Institute of Technology, 77 Massachusetts Avenue,
Cambridge, MA 02179, USA
2
Department of Pathology, Brigham and Women’s Hospital, 75 Francis Street, Boston, MA 02115, USA
3
Department of Pathology, Massachusetts General Hospital, Boston, MA 02114, USA
4
Department of Obstetrics and Gynecology, Boston Medical Center, 85 East Concord Street, Boston, MA 02118, USA
*[email protected]
Abstract: This study develops a spectroscopic algorithm for detection of
cervical high grade squamous intraepithelial lesions (HSILs). We collected
reflectance and fluorescence spectra with the quantitative spectroscopy
probe to measure nine spectroscopic parameters from 43 patients
undergoing standard colposcopy with directed biopsy. We found that there
is improved accuracy for distinguishing HSIL from non-HSIL (low grade
SIL and normal tissue) when we “normalized” spectroscopy parameters by
dividing the values extracted from each clinically determined suspicious site
by the corresponding value extracted from a clinically normal squamous site
from the same patient. The “normalized” scattering parameter (A) at 700nm,
best distinguished HSIL from non-HSIL with sensitivity and specificity of
89% and 79% suggesting that a simple, monochromatic instrument
measuring only A may accurately detect HSIL.
© 2011 Optical Society of America
OCIS codes: (170.0170) Medical optics and biotechnology; (170.6510) Spectroscopy, tissue
diagnostics
References and links
1.
M. Sideri, N. Spolti, L. Spinaci, F. Sanvito, R. Ribaldone, N. Surico, and L. Bucchi, “Interobserver variability of
colposcopic interpretations and consistency with final histologic results,” J. Low. Genit. Tract Dis. 8(3), 212–216
(2004).
2. N. M. Marín, A. Milbourne, H. Rhodes, T. Ehlen, D. Miller, L. Benedet, R. Richards-Kortum, and M. Follen,
“Diffuse reflectance patterns in cervical spectroscopy,” Gynecol. Oncol. 99(3 Suppl 1), S116–S120 (2005).
3. S. K. Chang, I. Pavlova, N. M. Marín, M. Follen, and R. Richards-Kortum, “Fluorescence spectroscopy as a
diagnostic tool for detecting cervical pre-cancer,” Gynecol. Oncol. 99(3 Suppl 1), S61–S63 (2005).
4. S. K. Chang, N. Marin, M. Follen, and R. Richards-Kortum, “Model-based analysis of clinical fluorescence
spectroscopy for in vivo detection of cervical intraepithelial dysplasia,” J. Biomed. Opt. 11(2), 024008 (2006).
5. R. J. Nordstrom, L. Burke, J. M. Niloff, and J. F. Myrtle, “Identification of cervical intraepithelial neoplasia
(CIN) using UV-excited fluorescence and diffuse-reflectance tissue spectroscopy,” Lasers Surg. Med. 29(2),
118–127 (2001).
6. N. Ramanujam, M. F. Mitchell, A. Mahadevan, S. Thomsen, A. Malpica, T. Wright, N. Atkinson, and R.
Richards-Kortum, “Development of a multivariate statistical algorithm to analyze human cervical tissue
fluorescence spectra acquired in vivo,” Lasers Surg. Med. 19(1), 46–62 (1996).
7. R. D. Alvarez, T. C. Wright, and Optical Detection Group, “Effective cervical neoplasia detection with a novel
optical detection system: a randomized trial,” Gynecol. Oncol. 104(2), 281–289 (2007).
8. W. K. Huh, R. M. Cestero, F. A. Garcia, M. A. Gold, R. S. Guido, K. McIntyre-Seltman, D. M. Harper, L. Burke,
S. T. Sum, R. F. Flewelling, and R. D. Alvarez, “Optical detection of high-grade cervical intraepithelial neoplasia
in vivo: results of a 604-patient study,” Am. J. Obstet. Gynecol. 190(5), 1249–1257 (2004).
9. I. Georgakoudi, E. E. Sheets, M. G. Müller, V. Backman, C. P. Crum, K. Badizadegan, R. R. Dasari, and M. S.
Feld, “Trimodal spectroscopy for the detection and characterization of cervical precancers in vivo,” Am. J.
Obstet. Gynecol. 186(3), 374–382 (2002).
10. Y. N. Mirabal, S. K. Chang, E. N. Atkinson, A. Malpica, M. Follen, and R. Richards-Kortum, “Reflectance
spectroscopy for in vivo detection of cervical precancer,” J. Biomed. Opt. 7(4), 587–594 (2002).
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2917
11. J. R. Mourant, T. J. Bocklage, T. M. Powers, H. M. Greene, K. L. Bullock, L. R. Marr-Lyon, M. H. Dorin, A. G.
Waxman, M. M. Zsemlye, and H. O. Smith, “In vivo light scattering measurements for detection of precancerous
conditions of the cervix,” Gynecol. Oncol. 105(2), 439–445 (2007).
12. I. M. Orfanoudaki, G. C. Themelis, S. K. Sifakis, D. H. Fragouli, J. G. Panayiotides, E. M. Vazgiouraki, and E.
E. Koumantakis, “A clinical study of optical biopsy of the uterine cervix using a multispectral imaging system,”
Gynecol. Oncol. 96(1), 119–131 (2005).
13. S. B. Cantor, J. M. Yamal, M. Guillaud, D. D. Cox, E. N. Atkinson, J. L. Benedet, D. Miller, T. Ehlen, J. Matisic,
D. van Niekerk, M. Bertrand, A. Milbourne, H. Rhodes, A. Malpica, G. Staerkel, S. Nader-Eftekhari, K. AdlerStorthz, M. E. Scheurer, K. Basen-Engquist, E. Shinn, L. A. West, A. T. Vlastos, X. Tao, J. R. Beck, C.
Macaulay, and M. Follen, “Accuracy of optical spectroscopy for the detection of cervical intraepithelial
neoplasia: Testing a device as an adjunct to colposcopy,” Int. J. Cancer 128(5), 1151–1168 (2011).
14. J. R. Mourant, T. M. Powers, T. J. Bocklage, H. M. Greene, M. H. Dorin, A. G. Waxman, M. M. Zsemlye, and
H. O. Smith, “In vivo light scattering for the detection of cancerous and precancerous lesions of the cervix,”
Appl. Opt. 48(10), D26–D35 (2009).
15. J. R. Mourant, T. J. Bocklage, T. M. Powers, H. M. Greene, M. H. Dorin, A. G. Waxman, M. M. Zsemlye, and
H. O. Smith, “Detection of cervical intraepithelial neoplasias and cancers in cervical tissue by in vivo light
scattering,” J. Low. Genit. Tract Dis. 13(4), 216–223 (2009).
16. C. Redden Weber, R. A. Schwarz, E. N. Atkinson, D. D. Cox, C. Macaulay, M. Follen, and R. Richards-Kortum,
“Model-based analysis of reflectance and fluorescence spectra for in vivo detection of cervical dysplasia and
cancer,” J. Biomed. Opt. 13(6), 064016 (2008).
17. M. Cardenas-Turanzas, J. A. Freeberg, J. L. Benedet, E. N. Atkinson, D. D. Cox, R. Richards-Kortum, C.
MacAulay, M. Follen, and S. B. Cantor, “The clinical effectiveness of optical spectroscopy for the in vivo
diagnosis of cervical intraepithelial neoplasia: where are we?” Gynecol. Oncol. 107(1 Suppl 1), S138–S146
(2007).
18. A. Blaustein and R. J. Kurman, Blaustein's pathology of the female genital tract (Springer, New York, 2002).
19. R. Kalluri and M. Zeisberg, “Fibroblasts in cancer,” Nat. Rev. Cancer 6(5), 392–401 (2006).
20. H. Nagase and J. F. Woessner, Jr., “Matrix metalloproteinases,” J. Biol. Chem. 274(31), 21491–21494 (1999).
21. J. Mazibrada, M. Rittà, M. Mondini, M. De Andrea, B. Azzimonti, C. Borgogna, M. Ciotti, A. Orlando, N.
Surico, L. Chiusa, S. Landolfo, and M. Gariglio, “Interaction between inflammation and angiogenesis during
different stages of cervical carcinogenesis,” Gynecol. Oncol. 108(1), 112–120 (2008).
22. C. K. Brookner, M. Follen, I. Boiko, J. Galvan, S. Thomsen, A. Malpica, S. Suzuki, R. Lotan, and R. RichardsKortum, “Autofluorescence patterns in short-term cultures of normal cervical tissue,” Photochem. Photobiol.
71(6), 730–736 (2000).
23. J. A. Freeberg, D. M. Serachitopol, N. McKinnon, R. Price, E. N. Atkinson, D. D. Cox, C. MacAulay, R.
Richards-Kortum, M. Follen, and B. Pikkula, “Fluorescence and reflectance device variability throughout the
progression of a phase II clinical trial to detect and screen for cervical neoplasia using a fiber optic probe,” J.
Biomed. Opt. 12(3), 034015 (2007).
24. C. Brookner, U. Utzinger, M. Follen, R. Richards-Kortum, D. Cox, and E. N. Atkinson, “Effects of biographical
variables on cervical fluorescence emission spectra,” J. Biomed. Opt. 8(3), 479–483 (2003).
25. S. K. Chang, M. Y. Dawood, G. Staerkel, U. Utzinger, E. N. Atkinson, R. R. Richards-Kortum, and M. Follen,
“Fluorescence spectroscopy for cervical precancer detection: Is there variance across the menstrual cycle?” J.
Biomed. Opt. 7(4), 595–602 (2002).
26. C. K. Brookner, U. Utzinger, G. Staerkel, R. Richards-Kortum, and M. F. Mitchell, “Cervical fluorescence of
normal women,” Lasers Surg. Med. 24(1), 29–37 (1999).
27. E. M. Gill, A. Malpica, R. Richards-Kortum, M. Follen, and N. Ramanujam, “Collagen autofluorescence of the
human cervix and menopausal status,” Lasers Surg. Med. 32(Suppl. 15), 12 (2003) (abstract).
28. S. K. Chang, Y. N. Mirabal, E. N. Atkinson, D. Cox, A. Malpica, M. Follen, and R. Richards-Kortum,
“Combined reflectance and fluorescence spectroscopy for in vivo detection of cervical pre-cancer,” J. Biomed.
Opt. 10(2), 024031 (2005).
29. J. Mirkovic, C. Lau, S. McGee, C. C. Yu, J. Nazemi, L. Galindo, V. Feng, T. Darragh, A. de Las Morenas, C.
Crum, E. Stier, M. Feld, and K. Badizadegan, “Effect of anatomy on spectroscopic detection of cervical
dysplasia,” J. Biomed. Opt. 14(4), 044021 (2009).
30. C. P. Crum, M. R. Nucci, and K. R. Lee, Diagnostic Gynecologic and Obstetric Pathology (Elsevier,
Philadelphia, 2011).
31. G. Zonios, L. T. Perelman, V. M. Backman, R. Manoharan, M. Fitzmaurice, J. Van Dam, and M. S. Feld,
“Diffuse reflectance spectroscopy of human adenomatous colon polyps in vivo,” Appl. Opt. 38(31), 6628–6637
(1999).
32. M. G. Müller, I. Georgakoudi, Q. G. Zhang, J. Wu, and M. S. Feld, “Intrinsic fluorescence spectroscopy in turbid
media: disentangling effects of scattering and absorption,” Appl. Opt. 40(25), 4633–4646 (2001).
33. C. Lau, “Detecting cervical dysplasia with quantitative spectroscopic imaging,” Ph.D. thesis (Massachusetts
Institute of Technology, Cambridge, MA, 2009).
34. D. Arifler, C. MacAulay, M. Follen, and R. Richards-Kortum, “Spatially resolved reflectance spectroscopy for
diagnosis of cervical precancer: Monte Carlo modeling and comparison to clinical measurements,” J. Biomed.
Opt. 11(6), 064027 (2006).
35. D. G. Ferris, Modern Colposcopy: Textbook and Atlas (Kendall/Hunt, Dubuque, Iowa, 2004).
36. W. Choi, C. C. Yu, C. Fang-Yen, K. Badizadegan, R. R. Dasari, and M. S. Feld, “Field-based angle-resolved
light-scattering study of single live cells,” Opt. Lett. 33(14), 1596–1598 (2008).
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2918
1. Introduction
The main target of the clinical management of women with suspected squamous
intraepithelial lesions (SIL) is the accurate diagnosis of precancerous changes, specifically
high grade SIL (HSIL). The current clinical standard for diagnosis of HSIL is colposcopy, a
procedure that involves visual inspection and biopsy of at-risk tissue, followed by
histopathological diagnosis. The diagnostic accuracy of colposcopy greatly depends on the
physician’s expertise and even when conducted by experts, is subject to significant diagnostic
variability [1]. Spectroscopy is a technique that may reduce the interobserver disagreement of
colposcopy and improve its diagnostic accuracy by diagnosing HSIL in an objective manner.
The effectiveness of spectroscopic techniques, specifically reflectance and fluorescence, for in
vivo diagnosis of HSIL has been extensively evaluated [2–16] These studies demonstrate the
potential of spectroscopy to improve the effectiveness of disease detection [17].
The spectroscopic diagnosis of cervical dysplasia is based on the contrast in tissue spectra
caused by loss of differentiation of the epithelial cells [18], degradation and reorganization of
stromal collagen by matrix metalloproteinase activity [19,20], increased metabolic activity,
and angiogenesis [21]. Tissue spectroscopy is not only affected by disease, but also by age
[15,22–26], menopausal status [15,23–27], time after the application of acetic acid [12], and
normal variations in cervical anatomy [6,23,28,29].
Historically, spectroscopic studies have included clinically normal squamous sites, either
non-biopsied or histopathologically confirmed, in the validation set for diagnosing HSILs
[5,6,8,10,28]. Mourant et al. [11,14] and Georgakoudi et al. [9] noted an apparent increase in
diagnostic power when clinically normal tissues were included in the validation set. Similarly,
Freeberg et al. [23] observed that tissue type influences both reflectance and fluorescence
measurements.
In a recent study by our laboratory, we demonstrated that underlying differences in tissue
anatomy can have a confounding effect on diagnostic spectral algorithms [29]. Normal
transformation zone of the cervix, the area where the vast majority of HSILs are found [30], is
anatomically, histologically, and spectroscopically different from the normal squamous
mucosa. As the vast majority of the HSILs are found in the transformation zone, the spectral
differences between normal squamous mucosa and HSIL are largely due to normal anatomical
differences. Based on the findings of this study, a common practice of including clinically
normal squamous sites into the data set which is used to develop or evaluate the performance
of the algorithm for detection of HSIL is a confounding artifact that artificially increases
performance values with respect to the key differentiation to be made, namely distinguishing
HSILs from clinically suspicious non-HSILs. The data in this study demonstrated the
confounding influence of including clinically normal squamous sites not only affects the
performance levels but also the number of specific spectroscopic parameters that can be used
in the diagnostic algorithm. The affected parameters included those describing the scattering,
absorption, and fluorescence properties of tissue. In order to properly evaluate the accuracy of
clinical disease detection, spectroscopic data must be analyzed within the appropriate
anatomical context.
The aim of the present study was to develop an algorithm for detection of HSILs free of
the confounding effect of cervical anatomy. We studied patients undergoing colposcopic
examination and used reflectance and fluorescence spectroscopy to differentiate HSILs from
non-HSILs among abnormal sites identified by the clinician as needing biopsy. Physical
models were used to fit the spectra and extract parameters related to tissue morphology and
biochemistry. We investigated the effect of per-patient parameter normalization on diagnostic
performance as well as the effect of normal anatomical variation within the transformation
zone, the glandular content, on the extracted spectroscopy parameters. The spectroscopy
parameters were then used to develop a spectroscopic diagnostic algorithm to distinguish
HSILs from non-HSILs.
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2919
2. Materials and methods
2.1. Data collection
Details of data collection and spectroscopic analysis of a cervical data set used in this study
were previously described by Mirkovic et al. [29]. Briefly, the clinical in vivo study was
conducted at the Boston Medical Center and involved 43 patients undergoing colposcopic
evaluation following an abnormal Pap smear. For each patient, reflectance and fluorescence
spectra were collected from a colposcopically normal squamous (CNSQ) site as well as
colposcopically abnormal sites using a fiber optic based clinical device developed by our
laboratory known as the Fast Excitation Emission Matrix (FastEEM). The instrument and the
calibration procedures have been previously described. 20 After the application of acetic acid
(5% solution) to the cervix during colposcopy, the probe which samples an area of tissue ~1
mm in diameter was brought into gentle contact with the tissue. The reflectance and
fluorescence spectra were acquired in approximately three seconds. Two to three
measurements were acquired for each tissue site. Colposcopically abnormal sites were then
biopsied and evaluated by histopathology. Clinically normal squamous sites were not
biopsied.
2.2. Histopathology
Each biopsy specimen underwent standard histopathological processing. In order to minimize
inter-observer diagnostic variability, hematoxylin and eosin stained tissue sections were
evaluated independently by three experienced pathologists (CC, ADLM, TD) using standard
diagnostic criteria. Consensus diagnosis (agreement between two of the three pathologists)
was used as the diagnostic gold standard. Each biopsied site was classified as either HSIL or
non-HSIL (negative for SIL or low grade squamous intraepithelial lesion, LSIL).
All histologic specimens were further examined by a single pathologist (CC) for the
absence or presence of features consistent with the transformation zone. If the stroma (the
connective tissue underlying the epithelium) of a particular site was visible, we further
performed a qualitative assessment of its glandular content. Each site was classified as having
either a significant glandular content or a minimal glandular content based on whether the
ratio of the area occupied by glands to area occupied by stroma was ≥0.25 or <0.25. Finally,
the average epithelial thickness was measured with Zeiss Axio Imager 2.0.0.0. software and
defined by an average value of three measurements across the surface epithelium.
2.3. Spectral data analysis
Four patients were excluded due to instrument malfunctions during measurement (CCD
camera overheat, probe damage). Raw spectra for each set of measurements were examined
and those with poor overlap between repeat measurements were excluded. We excluded 3
study sites for which all sets in a measurement were inconsistent (>10% average standard
deviation between measurements), as well as 4 sites for which the tissue started bleeding due
to probe contact.
We used physically-based models to extract the spectroscopy parameters from the tissue
reflectance and fluorescence spectra. The reflectance spectra were analyzed using the diffuse
scattering model developed by Zonios et al. [31], and tissue fluorescence emission spectra
were analyzed by the photon-migration model developed by Muller et al. [32]. The details of
spectral data analysis were further described by Mirkovic et al. [29]. As a result, we derived
nine spectroscopic parameters from modeling tissue reflectance and fluorescence: scattering
parameters (A [mm−1], B, and C [mm−1]), hemoglobin concentration Hb [mg/ml], oxygen
saturation α, effective blood vessel radius bvr [mm], concentration of beta-carotene β-car
[mg/ml], and the fractional contributions of collagen and NADH in the intrinsic fluorescence
(Coll and NADH, respectively). We note that the A parameter is equivalent to the reduced
scattering coefficient at 700 nm.
To identify changes in spectroscopic parameters due to disease, we studied the values of
extracted spectroscopy parameters from clinically suspicious sites. During colposcopy,
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2920
abnormal sites are identified based on contrasts in color, texture, and other features relative to
normal tissue. We evaluated whether a similar procedure would be useful for a spectroscopicbased diagnostic method. Specifically, we divided the spectroscopy parameters extracted from
each clinically suspicious site by the values of the corresponding spectroscopy parameters
extracted from a CNSQ site collected from the same patient. Parameters derived from this
procedure are subsequently referred to as normalized spectroscopy parameters.
Normalized spectroscopy parameters were correlated to the histopathology diagnosis for
all data collected from clinically suspicious sites. A two-sided Wilcoxon Rank Sum test was
used to test the hypothesis that the extracted normalized spectroscopic parameter distributions
of HSIL and non-HSIL were different. A p-value of <0.05 was considered significant. The
spectral algorithms were developed using logistic regression models to identify the significant
spectroscopic parameters providing the diagnostic information. The likelihood ratio test was
used to assess the significance of each of the parameters in the logistic regression model. 21 A
p-value <0.05 was considered to be significant. Leave-one-out cross-validation (LCV) was
used to construct receiver-operator characteristic (ROC) curves for the spectral algorithms.
The discrimination ability was evaluated by the area under the ROC curve (AUC), as well as
the sensitivity and specificity. In the following, we report a point on the ROC curve which is
the shortest distance away from the point of perfect separation (100% sensitivity and 100%
specificity) defined by
  sensitivity  2  specificity  2 
(1)
min  1 −
 + 1 −
 
100
100
 


 

We refer to this point whenever we quote sensitivity and specificity values.
To study the effect of tissue glandular content on the spectroscopy parameters, we divided
non-HSIL sites into two groups: 1) non-HSIL sites with a gland-to-stroma ratio of <0.25 (nonGS sites), and 2) non-HSIL sites with gland-to-stroma ratio of ≥0.25 (GS sites), and compared
them to all HSIL sites by using the statistical methods (two-sided Wilcoxon Rank Sum test
and LCV and logistic regression) described above.
3. Results
3.1. Data set
As shown in Table 1, our data set consisted of 33 CNSQ sites, which were not biopsied, and
51 clinically suspicious biopsied sites, out of which histopathology determined that 9 sites
(from 6 patients) were HSILs and 42 sites were non-HSIL (30 sites negative for SIL from 19
patients and 12 LSILs from 11 patients). We emphasize that the non-HSIL sites in our data set
do not include the 33 CNSQ sites. The patient age for this data set ranges from 18 to 47 years,
and the mean patient age is 26 ± 7.5 years.
Table 1. Data seta
Clinical Category
Normal (CNSQ)
Histology Category
No. of Sites
Not biopsied
33
Negative for SIL
30
non-HSIL
Suspicious
LSIL
12
HSIL
9
a
Clinically normal squamous, CNSQ; squamous intraepithelial lesions.
SIL; high grade SIL, HSIL; low grade SIL, LSIL.
3.2. Microscopic characterization
Histopathological evaluation confirmed that 36 of 51 biopsied sites were from the
transformation zone. Fifteen sites could not be histologically confirmed as transformation
zone (e.g., stroma was not visible on the histology slides to ensure full assessment or
glandular elements were not present). All of the HSIL sites, except one for which stroma was
not visible, were confirmed to be from the transformation zone.
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2921
Table 2 provides a description of glandular content for non-HSIL and HSIL sites. High
glandular content (gland-to-stroma ratio of ≥0.25) was found in 5/8 (62.5%) of HSIL sites
compared to 13/34 (38%) of non-HSIL sites, however this difference was not significant by
Wilcoxon ransum test. There was no significant difference in epithelial thickness for HSIL
and non-HSIL sites (171 ± 50 and 250 ± 124 μm, respectively).
Table 2. Description of glandularity for non-HSIL and HSIL sites
Group
non-HSIL
HSIL
Glandular content (gland-to-stroma ratio)
≥0.25 (GS) <0.25 (non-GS) Could not be evaluated
13
21
8
5
3
1
Fig. 1. Discrimination of HSIL from non-HSIL among clinically suspicious sites. Boxplots of
normalized (a) A parameter (reduced scattering coefficient at 700nm), (b) α (oxygen
saturation), (c) bvr (blood vessel radius), (d) Hb (hemoglobin concentration), (e) Coll
(fractional contribution of collagen to intrinsic fluorescence); (f) Receiver operator
characteristic curve for the diagnostic algorithm (normalized A parameter only). Box plots:
median (horizontal line within the box), upper and lower quartiles (upper and lower edges of
the box, respectively), extent of the data (whiskers), and outliers (crosses, data points that are
more than 1.5 times the interquartile range below the lower quartile or above the upper
quartile).
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2922
3.3. Identifying HSILs among the clinically suspicious sites
To assess the potential clinical impact of our technique, it is essential to evaluate its success in
differentiating HSIL from non-HSIL sites among clinically suspicious sites, most of which are
found in the transformation zone.
Recent work in our laboratory, which uses the same data set described in this paper, have
shown that HSIL sites were characterized by significantly lower values of the A and Coll, and
significantly higher values of Hb compared to the non-HSIL sites. The AUC, sensitivity and
specificity of 0.65, 78%, and 57% were achieved on the basis of A parameter. Combination of
Coll and Hb parameters produced similar AUC, sensitivity and specificity (0.68, 78% and
67%, respectivelly) [29]
We find that after per-patient normalization, HSIL sites are characterized by significantly
lower values of the A parameter and significantly higher values of α, Hb, and bvr compared to
non-HSIL sites. AUC, sensitivity and specificity of 0.84, 89% and 79%, respectively, were
achieved. The positive and negative predictive values were 48% and 97%, respectively. The
normalized A parameter was the most diagnostic and the only parameter retained in the
logistic regression algorithm. The box plots of normalized A, α, bvr, and Hb which have
statistically significant differences between non-HSIL and HSIL sites, and Coll which has no
statistically significant difference between non-HSIL and HSIL are shown in Figs. 1(a)-1(e),
respectively, and the ROC plot based on the normalized A parameter is shown in Fig. 1(f).
CNSQ sites are significantly different from both non-HSIL and HSIL sites for all parameters
shown.
3.4. Effect of glandular content on spectroscopic parameters
Because the glandular content varies within the transformation zone, we also investigated the
effect of gland-to-stroma ratio on the diagnostic normalized spectroscopy parameters. While
all HSIL can be differentiated from non-GS sites by the lower values of A and Coll and higher
values of Hb, α and bvr, only two parameters, A and α, were significantly different between
HSIL sites and GS sites based on the Wilcoxon Rank Sum test. Figure 2 shows box plots of
the A and α parameters. The A parameter was significantly different between GS and non-GS
sites, while α was not significantly different. We also developed logistic regression models to
differentiate all HSIL from non-GS and GS sites. In both cases, A alone provided the best
discrimination between the two sites and the impact of other parameters was negligible. AUC,
sensitivity, and specificity for differentiating all HSIL from non-GS were 0.84, 89% and 79%,
respectively. AUC, sensitivity, and specificity for differentiating all HSIL from GS sites were
0.82, 89% and 70%, respectively.
Fig. 2. Discrimination of HSIL from GS and non-GS sites. Box plots of normalized (a) A
parameter and (b) α.
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2923
4. Comment
Both disease and normal variations in microscopic anatomy are significant sources of
spectroscopic contrast in clinically obtained tissue spectra. In order to properly evaluate the
accuracy of disease detection, spectroscopic data must therefore be analyzed within the
appropriate anatomical context. This study specifically focuses on differentiating HSILs from
non-HSILs among clinically suspicious sites, the majority of which are found within the
transformation zone. We find that after normalization by an internal standard, the A parameter
alone provided the best diagnostic performance in differentiating HSIL from non-HSIL sites.
AUC, sensitivity and specificity of 0.84, 89% and 79%, respectively, were achieved. Positive
and negative predictive values were 48% and 97%, respectively. The high negative predictive
value suggests that this technique may be useful for reducing the number of unnecessary
biopsies. Even though the spectroscopy parameters including A parameter are affected by
glandular content, the A parameter was the most diagnostic parameter in the discrimination of
HSIL from both GS and non-GS sites.
In our study HSIL sites exhibit significantly lower values of A parameter relative to the
non-HSIL sites. This result is in agreement with results from similar studies in the literature.
In a study of 161 patients, Mirabal et al. [10] found that there is a gradual decrease in mean
reflectance intensity as the severity of dysplasia increases. In studies by Nordstrom et al. [5],
and Huh et al. [8], reflectance was found to differentiate between HSIL and normal sites in
the transformation zone (squamous metaplasia), while fluorescence did not yield significant
differences. For both studies it is not known whether the differences in reflectance spectra
were due to a higher hemoglobin concentration, lower scattering, or a combination of the two
effects. Furthermore, our study cannot be directly compared to these two studies, as our study
compares HSIL to all clinically suspicious non-HSIL sites, including the LSIL sites, while
their studies report LSIL and squamous metaplasia sites separately. Georgakoudi et al. [9].
also report lower reduced scattering coefficient (similar to A parameter) for distinguishing
SILs from biopsied non-SILs. However, we cannot directly compare their findings to those of
this study as they did not discriminate HSIL from non-HSIL. Finally, the findings of the
follow-up clinical in vivo study conducted with the Quantitative Spectroscopy Imaging
system (manuscript in preparation) were consistent with the findings of our study. This study
also observed that after normalization by an internal standard, the A parameter alone provided
the best diagnostic performance in differentiating HSIL from non-HSIL sites [33].
The lower value of the A parameter for HSIL sites compared to non-HSIL sites is also
physically justified. Arifler et al. [34] used Monte Carlo modeling of cervical tissue to show
that the smaller stromal reduced scattering coefficient is the major cause for decreased
reflectance intensity of HSIL compared to normal squamous tissue. Degradation of stromal
collagen by matrix metalloproteinase activity [19,20] is the likely explanation for the lower
value of A parameter for HSIL sites compared to non-HSIL sites.
We also observe higher hemoglobin concentration of HSIL sites relative to the non-HSIL
sites. Higher hemoglobin concentration in HSIL sites compared to other tissue types has been
noted by Chang et al. [4] Additionally, Marin et al. [2] report that hemoglobin features of the
reflectance tissue spectra are more prominent in abnormal tissue compared to normal
squamous tissue. However, studies that considered diagnosing HSIL within clinically
suspicious sites, such as Georgakoudi et al. [9], as well as Mourant et al. [11] reported no
significant change in the hemoglobin concentration between HSIL and non-HSILs.
Our finding of higher hemoglobin oxygenation for HSIL sites compared to non-HSIL
within the clinically suspicious sites is consistent with the results of a study by Mourant et al.
[11] which also looked at the difference between HSIL and clinically suspicious non-HSIL
sites, 90% of which were found in the transformation zone. The source of higher hemoglobin
oxygenation for HSIL sites is not well understood and needs further investigation.
We find that the effective blood vessel radius is increased for HSIL sites compared to nonHSIL sites. This may be due to the presence of dilated atypical blood vessels associated with
precancerous and cancerous changes [35].
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2924
Finally, we observe decreased Coll for HSIL sites compared to non-HSIL sites. This
observation is consistent with decreased collagen fluorescence due to degradation of collagen
matrix, increased NADH fluorescence due to changes in cellular metabolism, or a
combination of both. The increase in epithelial thickness is not a source of this feature, since
there was no significant difference in measured epithelial thickness between HSIL and nonHSIL sites in our study. Increased NADH contribution of SILs compared to non-SILs within
the transformation zone has been observed by Georgakoudi et al. [9] Chang et al. [4] report a
decreased stromal collagen contribution; however, their study included clinically normal
squamous sites. Studies by Nordstrom [5], and Huh [8], which utilize 340 nm fluorescence,
reported no significant differences between HSIL and normal sites in the transformation zone
(squamous metaplasia). A study of Ramanujam et al. reported that 340 nm excitation HSIL
sites could not be differentiated from non-HSIL sites in the transformation zone (cervical
intraepithelial neoplasia 2/3 (equivalent to HSIL) vs. squamous metaplasia).
We found that normalization of the spectroscopy parameters enhanced the contrast
between HSIL and non-HSIL sites. Normalization may reduce spectroscopic variations due to
intrinsic patient-to-patient variations associated with age, hormonal contraception, and
menopausal status. Furthermore, it may account for differences caused by the time-dependent
effect of acetic acid on tissue scattering and absorption. The vasoconstrictive and light
scattering effects of acetic acid [35,36] may affect the extracted hemoglobin concentration,
effective blood vessel radius, and also the scattering parameters. Recent work in our
laboratory, which uses the same data set described in this paper, showed that without
parameter normalization, HSIL sites could be differentiated from non-HSIL with AUC,
sensitivity, and specificity of only 0.68, 78% and 67%, respectively [29]. In the present study,
we found that parameter normalization resulted in substantial improvements performance
metrics, as reported above. However, we point out that per-patient normalization of Coll
parameter has decreased the ability of this parameter to differentiate between non-HSIL and
HSIL sites. Further investigation is required to determine the best strategy for fluorescence
per-patient normalization.
The finding that only the A parameter has diagnostic importance suggests that a
significantly simpler, faster, and less expensive instrument which measures tissue scattering
using one wavelength may be all that is required to reliably detect cervical disease. The
limitation of our study is a relatively small number of patients. If the results of our study are
further confirmed in the ongoing larger imaging clinical study, our laboratory will design a
simplified instrument for detecting cervical dysplasia and investigate how effective this
approach is in improving the accuracy of cervical dysplasia detection. In developed countries,
this simple instrument could be used as an adjunct to colposcopy to reduce the number of
unnecessary biopsies. However, the greatest impact of this simple and relatively inexpensive
instrument would be on cervical cancer diagnosis in developing countries, where the lack of
medical infrastructure precludes cytology-based cervical cancer screening program. In these
settings, the common mode of cervical cancer screening is by visual inspection after
application of acetic acid (VIA) followed by immediate treatment of suspicious lesions. VIA
has a significant false positive rate. The simple spectroscopic instrument could be used as an
adjunct to VIA to improve accuracy in the diagnosis of cervical cancer and its precursors.
Acknowledgments
We thank Chung-Chieh Yu and Jonathan Nazemi for valuable discussions about data
modeling. We thank Jonathan Nazemi and Luis Galindo for the engineering assistance, and
Victoria Feng for the technical assistance. We finally thank Teresa Darragh and Antonio de
las Morenas for their valuable contribution to the pathology evaluation. This research was
funded by the National Institutes of Health grant R01 CA097966 and the Laser Biomedical
Research Center grant P41 RR02594.
#150531 - $15.00 USD
(C) 2011 OSA
Received 11 Jul 2011; revised 1 Sep 2011; accepted 7 Sep 2011; published 29 Sep 2011
1 October 2011 / Vol. 2, No. 10 / BIOMEDICAL OPTICS EXPRESS 2925